Dissertation
submitted to the
Combined Faculties for the Natural Sciences and for Mathematics
of the Ruperto‐Carola University of Heidelberg, Germany
for the degree of
Doctor of Natural Sciences
Presented by
Master of Sciences Philipp Konstantin Zimmermann
Born in Berlin‐Zehlendorf
Oral examination: April 16th, 2015
Genome‐wide detection of induced DNA double strand breaks
Referees:
Prof. Dr. Christof von Kalle
Prof. Dr. Stefan Wiemann
I
1. INTRODUCTION 1
1.1 The DNA damage response and genomic instability 1 1.1.1 DNA damaging agents and the DNA damage response 1
1.2 DNA double‐strand break (DSB) repair pathways 3 1.2.1 The Non‐Homologous End Joining (NHEJ) Repair Pathway 4 1.2.2 Methods for the detection of DNA damage and DNA repair activity 6
1.3 Radio‐ and chemotherapy 7 1.3.1 Types of ionizing radiation 7 1.3.2 Radiation‐induced DNA damages 8 1.3.3 The topoisomerase family 9 1.3.4 Topoisomerase 2 catalytic cycle and targeting by anticancer drugs 10 1.3.5 Cancer therapy‐induced delayed genomic instability 11
1.4 Lentiviruses 11 1.4.1 History and phylogeny of lentiviruses 11 1.4.2 The lentiviral genome 12 1.4.3 The life cycle of lentiviruses 13 1.4.4 Structure of lentiviral vectors for gene therapy 15
1.5 Scientific aims 16
2. MATERIALS AND METHODS 18
2.1 Materials 18 2.1.1 Chemicals 18 2.1.2 Enzymes 19 2.1.3 Bacteria 19 2.1.4 Cell lines and primary cells 19 2.1.5 Antibodies 20 2.1.6 Plasmids 20 2.1.7 Oligonucleotides 20 2.1.7.1 Standard primers for q‐RT‐PCR 20 2.1.7.2 Primers used for linker cassettes in LAM‐PCR 21 2.1.7.3 Primers used for LAM‐PCR 21 2.1.7.4 Fusionprimer for Pyrosequencing 21 2.1.7.5 Primers and oligos used for direct DSB labeling approaches 22 2.1.8 Commercial kits 22 2.1.9 Buffers, Media, Solutions 23 2.1.10 Disposables 24 2.1.11 Equipment 24 2.1.12 Software and data bases 25
2.2 Methods 26
II
2.2.1 Cell Culture Methods 26 2.2.1.1 Cell Cultivation 26 2.2.1.2 Freezing and thawing of cells 26 2.2.1.3 Cell Counting 26 2.2.1.4 Transfection 27 2.2.1.5 Transduction 27 2.2.1.6 Virus production 28 2.2.1.7 Determining the lentiviral titer on Hela cells 28 2.2.1.8 MTT Assay 28 2.2.1.9 Immunostaining of H2AX foci 29 2.2.1.10 Inhibition of NHEJ‐repair activity by Nu7441 and Mirin 29 2.2.1.11 Irradiation of cells 30 2.2.1.12 Inhibition of Topoisomerase 2 in mammalian cells with doxorubicin and etoposide 30 2.2.1.13 Preparation for FACS 30 2.2.1.14 Synchronization of NHDF‐A in G1/G0, S and G2/M phase of the cell cycle 31 2.2.2 Molecular Biology Methods 32 2.2.2.1 Isolation of genomic DNA from cultivated cells 32 2.2.2.2 Determining the DNA concentration 32 2.2.2.3 Polymerase Chain Reaction (PCR) 32 2.2.2.4 DNA agarose electrophoresis 33 2.2.2.5 DNA isolation from agarose gel 33 2.2.2.6 Absolute quantitative real‐time PCR (q‐RT‐PCR) 33 2.2.2.7 Linear‐Amplification Mediated Polymerase Chain Reaction (LAM‐PCR) 34 2.2.2.8 Cleaning‐Up of PCR products using AMPure XP beads 39 2.2.2.9 Fusionprimer‐PCR 39 2.2.2.10 SureSelect Target Enrichment for Illumina Multiplexed Sequencing 40 2.2.2.11 Tdt‐mediated labeling of DSB sites 44 2.2.2.12 Biotin Quantification 47 2.2.2.13 Linker‐Amplification‐Mediated DSB Trapping (LAM‐DST) 48 2.2.2.14 Pyrophosphate sequencing 50 2.2.2.15 Cloning of PCR amplicons using the TOPO‐TA Cloning Kit 50 2.2.2.16 Transformation of circular DNA into chemically‐competent E.coli 50 2.2.2.17 Mini‐ and maxipreparation of plasmid DNA 51 2.2.2.18 Enzymatic DNA restriction digest 51 2.2.3 Bioinformatical Methods 51 2.2.3.1 Automated Sequence Analysis (HISAP) 51 2.2.3.2 A549 mRNA expression analysis 52 2.2.3.3 DNaseI Hypersensitive Sites 52 2.2.3.4 Histone modifications and Transcription Factor Binding Sites 52 2.2.3.5 Ingenuity Pathway Analysis (IPA) 53 2.2.3.6 Identification of DSB site clusters in the genome 53
3. RESULTS 54
3.1 IDLV‐mediated capturing of radiation‐induced DSB sites in vivo 54
III
3.1.1 Immunostaining of H2AX foci in irradiated cells 54 3.1.2 MTT assay to determine lethal dose values for etoposide and doxorubicin 55 3.1.3 IDLV‐Delivered DNA‐baits tag radiation‐induced and repaired DSB sites 56 3.1.4 IDLV DSB trapping in NHDF‐A with impaired NHEJ‐repair activity 58 3.1.5 Trapping and mapping of TOP2 poison‐induced DSB 58 3.1.6 Calculating the number of integrated IDLV copies per irradiated cell 59 3.1.7 SureSelect Target Enrichment for analyzing IDLV vector integrity 60
3.2 Analyzing early DSB repair events and kinetics of DSB induction at single nucleotide resolution 61 3.2.1 Genomic tagging of early‐repaired radiation‐induced DSB sites by IDLV 62 3.2.2 Synchronization of NHDF‐A and Hela cells in G1, S and G2 phase 62 3.2.3 Tdt‐mediated labeling of radiation‐induced DSB sites 63 3.2.4 Linker‐Amplification‐Mediated DSB‐Trapping for DSB labeling in real‐time 66
3.3 DSB site distribution in radiation‐surviving and expandable cell populations 68 3.3.1 Identification of radiation‐induced DSB sites by LAM‐PCR 68 3.3.2 DSB are not enriched on chromosomes, in genes and gene‐regulatory regions 69 3.3.3 IDLV integration at radiation‐induced DSB sites is mediated by NHEJ‐repair 71
3.4 Analyzing the influence of transcriptional activity, chromatin status and gene classes and networks on DSB site distribution 72 3.4.1 Trapping of Radiation‐Induced DSB is not influenced by transcriptional activity 72 3.4.2 The location of radiation‐induced DSB sites is composed of histone modifications defining active chromatin 73 3.4.3 Radiation‐induced DSB in radiation‐survivor cells are enriched in genes and networks regulating cell survival 77 3.4.4 Identification and analysis of radiation‐induced DSB sites over time 79
3.5 Identification of frequently damaged and repaired genomic regions 81 3.5.1 DSB Trapping in irradiated and passaged cells reveals common regions of radiation‐induced and repaired damage 81 3.5.2 Radiation‐related DSB hotspots overlap with genes involved in maintaining genome stability and DNA repair 84 3.5.3 DSB hotspots overlap with eu‐ to heterochromatin border regions 86
4. DISCUSSION 88
4.1 Immunostaining of H2AX is not suitable to detect DSB and genomic instabilities in cancer therapy surviving cell populations 88
4.2 NHEJ‐mediated IDLV integration at DSB sites stably marks DNA damage and repair sites in living cells 89
4.3 Identification of radiation‐induced DSB sites 90 4.3.1 Transcriptional activity before irradiation does not influence DSB site distribution 90 4.3.2 DSB site distribution is non‐random with respect to the genome accessibility 91 4.3.3 Genes involved in specific cellular processes are enriched for induced DSB 93
IV
4.3.4 Clonality of DSB site distribution over time 93 4.3.5 Radiation‐induced and repaired DSB sites cluster in hotspots in specific genomic regions 94
4.4 Methods for in situ labeling of induced DSB sites 96
5. SUPPLEMENT 98
5.1 Supplementary Figures 98
5.2 SupplementaryTables 110
5.3 Figure Index 135 5.3.1 Figures 135 5.3.2 Supplementary Figures 136
5.4 Table Index 137 5.4.1 Tables 137 5.4.2 Supplementary Tables 137
5.5 Zusammenfassung 139
5.6 Summary 140
5.7 Abbreviations 141
5.8 References 146
5.9 Publications and congress attendances 152
6. DANKSAGUNG 154
1 INTRODUCTION
1. INTRODUCTION
1.1 The DNA damage response and genomic instability
1.1.1 DNA damaging agents and the DNA damage response
The DNA in the cell encodes the genetic information required for the functioning of all cells and living organisms. Every day, the DNA is under constant pressure to be destabilized by various processes and agents. These lesions can block DNA replication and transcription and are broadly divided according to their origin into either endogenous or exogenous (Figure 1) [1]. Endogenous processes such as DNA replication by DNA polymerases induce low levels of DNA damage. Other endogenous sources of DNA damage include genomic fragile sites, nucleases and reactive oxygen species (ROS) such as superoxide and hydrogen peroxide stemming from metabolic processes in the mitochondria [2]. These latter, highly reactive molecules form chemical bonds with other molecules within seconds of their production. Among their target molecules, the DNA is a susceptible target, in which ROS can cause base and sugar modifications, DNA‐protein crosslinks, single‐strand and double‐ strand breaks. In addition to endogenous processes, numerous exogenous sources also threaten the genomic integrity (Figure 1). The most pervasive form of exogenous DNA damaging agent is ultraviolet (UV) rays originating from sunlight that can hit the DNA directly and induce up to 100,000 DNA lesions per exposed cell [2]. These UV light generate various forms of DNA modifications, the most stable being the covalent link between two pyrimidine DNA bases [2]. X‐rays represent another type of DNA damaging agent, which is often used for imaging and cancer radiation‐therapy. These rays generate radicals in the DNA or in other cellular molecules that attack DNA bases, causing DNA oxidations as well as single‐strand and double‐strand breaks. Additional examples of exogenous DNA damaging agents include benzo‐α‐pyrene, polycyclic‐aromatic hydrocarbons and cancer chemotherapeutics that interfere with the DNA replication or the DNA damage repair machinery.
Along with the various types of DNA damages induced by endogenous processes and environmental agents, DNA double strand breaks (DSB) are the most dangerous DNA lesion [1]. In contrast to other types of DNA damage, DSB directly threaten genomic integrity, because they disrupt the continuity of the DNA. Failure to efficiently repair such DNA lesions can compromise genome integrity and result in a variety of genomic changes. Amongst others these include point mutations, chromosome number variations, gross chromosomal rearrangements such as translocations, amplifications, insertions, deletions, dimeric oncogenes and copy‐number variations, which can initiate neoplastic transformation [1]. In order to maintain genomic integrity and counteract the damage inflicted on the genome, the cell triggers a coordinated network of signaling cascades, which are collectively termed the DNA damage response (DDR) (Figure 1). 2 INTRODUCTION
Endogenous Exogenous Agents DNA Damaging Processes Agent Alkylating ROS Irradiation UV Agents
DNA Damage
ICL, DNA PD, Oxidation SSB, DSB adducts 6,4-PP
Sensor DNA damage Sensor Proteins
Checkpoint DNA Damage Checkpoints
Chromatin Remodelling Transcription DNA Repair Responses Apoptosis Senescence Cell Cycle Arrest
Figure 1: DNA damaging agents and the DNA damage response in mammalian cells. DNA damage can either arise by endogenous processes such as inflammation, reactive oxygen species, and DNA replication or can be induced by irradiation, UV light, or chemicals. The DNA damage inflicted is diverse, ranging from oxidized DNA bases to interstrand cross links (ICL), DNA adducts, single‐strand (SSB) and double‐strand breaks (DSB), pyrimidine dimers (PD) and 6,4‐photoproducts (PP). These damages activate DNA damage sensors that in turn activate various cellular responses which are collectively termed the DNA damage response (DDR). In addition to pathways dedicated to removing DNA modifications by DNA repair, cells have evolved several pathways to activate cell cycle checkpoints, block or induce transcription and remodel local chromatin structures. Moreover, if the DNA damage is too severe, apoptosis is induced. Image modified from [3].
The DDR can be divided into different sequential steps. First, the DNA damage sensor proteins of the DDR sense DNA lesions and bind to the damaged site. Subsequently, these proteins transmit the signal of the DNA damage to effector proteins by modifying these proteins post‐translationally. The phosphorylation, acetylation, ubiquitination and sumolyation of the effector proteins leads to an amplification of the damage signal. This signalling blocks cell cycle progression and allows the cell sufficient time to repair the damage. Additionally, the transcription of DDR‐related proteins can be activated and the transcription of non‐DDR‐related proteins as well as replication blocked. Furthermore, the DDR promotes alterations in local chromatin structure by post‐ translationally modifying the histone components in order to reveal the underlying DNA sequence and to recruit the DNA repair machinery (Figure 1). Histone modifications include phosphorylation, acetylation, methylation, and ubiquitination [4]. Cells that are defective in any of the aforementioned response mechanisms are more sensitive to DNA damaging agents, and many of such defects cause cancer, neurological defects and pre‐mature aging [1]. The first observation that inefficient DNA repair may increase the probability for cancer initiation was documented in 1968 by James Cleaver who reported that patients suffering from Xeroderma Pigmentosum (XP) have a defect in the DNA repair pathway responsible for repairing UV light‐induced DNA damages [5, 6]. Since this discovery, several cancer types stemming from mutations in the DNA damage response have been identified (Table 1). 3 INTRODUCTION
Table 1: Human disorders associated with defects in genome maintenance and enhanced cancer susceptibility. BER: base‐ excision repair; ICL: interstrand crosslink; MMR: mismatch repair; RECQ: recombination Q. Table taken and modified from [3] Disease Abbreviation Mutated Gene(s) Impaired Pathway Ataxia telangiectasia AT ATM DSB repair Atypical Werner WS WRN nuclear structure syndrome Bloom’s syndrome BLS BLM RECQ helicase Dyskeratosis DKC DKC1, TERC1 telomere maintenance congenita FANCA, B, C, D1 (BRCA2), D2, E, F, G, Fanconi anemia FA I, J (BRIP1), L, M, N (PALB2), O ICL repair (RAD51C), and P (SLX4) Li–Fraumeni many (p53 tumor p53 Syndrome suppressor inactivation) Nijmegen breakage NBS NBS1 DSB repair syndrome Rothmund–Thomson RTS RECQL4 RECQ helicase syndrome RECQ helicase, influencing Werner syndrome WS WRN nuclear structure, DSB repair, ICL repair, MMR, BER Xeroderma XP XPA‐G NER pigmentosum
The plethora of DNA damages induced by endogenous processes and exogenous agents necessitates the coordinated action of multiple distinct DNA repair pathways. Some DNA lesions can be directly reversed; most DNA damages however require the activity of several repair proteins and processing of the damaged DNA [2]. During DNA mismatch repair, a single strand break is induced upon DNA detection and the single strand removed before polymerase and ligase enzymes fill up the gap and reseal the DNA. In base‐excision repair, DNA glycosylase enzymes recognize the damaged DNA base, and initiate base removal and repair by nuclease, polymerase and ligase proteins. The nucleotide excision repair (NER) system recognizes helix‐distorting base lesions, excises a 22‐30 base oligonucleotide and thereby produces a single‐stranded DNA that is subsequently repaired. Upon repair of the DNA damage, the DDR proteins dissociate from the damaged and repaired siteallowing the cell to re‐enter the cell cycle [2]. If the DNA damage is too severe and cannot be efficiently repaired, cells can either engage in tolerance pathways which permit survival at the cost of mutagenesis [7] or induce cell death by apoptosis [1].
1.2 DNA double‐strand break (DSB) repair pathways
For the repair of DSB, two different mechanisms are present in the cell: Non‐Homologous End Joining (NHEJ) and Homologous Recombination (HR), which can be both subdivided into several pathways. The HR and NHEJ pathway differ mechanistically in several ways. HR repair is initiated by the generation of a single‐stranded DNA (ssDNA) overhang, promoted by the Mre11‐Rad50‐Nbs1 (MRN) complex and CtBP‐interacting protein (CtIP), whereas NHEJ‐repair is activated by binding of the Ku70/80 heterodimer to the DSB site. Moreover, NHEJ‐repair is considered error‐prone, because free DNA ends are quickly rejoined without requiring homology, whereas in HR the homologous sister chromatid is used as a template for copying the genomic information to the damaged DNA strand. Hence, in contrast to NHEJ, HR is not active throughout the cell cycle, but is restricted to late S and G2 phase when the homologous DNA template is available after replication. Thus, NHEJ is the dominant pathway 4 INTRODUCTION
for DSB repair in mammalian cells [2]. The exact cellular mechanisms determining which of the DNA repair pathway is used to repair a DSB are still not fully understood. However, recent work suggests that the choice between classical NHEJ and HR in replicating cells is regulated by DNA end resection [8]. Two regulators of the DSB repair pathway choice have emerged, namely the tumor suppressor proteins 53BP1 and BRCA1. 53BP1 contributes to NHEJ by interacting with chromatin at the DSB sites, thereby inhibiting DNA end resection and tethering the free DNA ends of the DSB in close proximity to promote their ligation [9]. Moreover, 53BP1 binds dimethylated histone H4 (H4K20me2), thereby stabilizing a chromatin conformation that is non‐permissive to nuclease access and limiting DNA end resection of the DSB intermediates [10]. Since in S/G2 phase the level of HR increases, mechanisms exist that block or reduce the activity of 53BP1 at DSB sites in order to promote HR. A key protein in this process is BRCA1; however, the exact mechanisms of BRCA1‐mediated 53BP1 inhibition and activation of HR at DSB sites are still unknown. It has been shown that BRCA1 stabilizes CtIP, a key molecule required for DSB end resection that promotes HR [11, 12]. Furthermore, BRCA1 may also influence the local abundance of H4K20me2, which prevents 53BP1 enrichment and NHEJ‐repair [13]. Other results suggest that BRCA1 also increases the level of ubiquitylation at DSB sites which may contribute to a chromatin status promoting HR by granting access of the resection machinery [9].
The DNA repair activity and repair kinetics vary in the different compartments of the genome [14]. Densely compacted heterochromatin (HC) was shown to be refractory to DNA repair factors such as γH2AX. Furthermore, DSB sites in heterochromatin, gene poor or pericentromeric regions in the genome are repaired with slower kinetics than DSB in euchromatin [15]. Thus, it has been hypothesized that the slower DSB repair kinetics in HC are due to hindered access of DNA repair factors to these dense chromatin regions [14]. However, Jakob and colleagues demonstrated that H2AX is phosphorylated inside HC, but that the damaged site is subsequently relocated to regions of lower chromatin density to enable efficient DSB repair [16]. Another factor influencing the kinetics of DSB repair is the chemical DNA damage complexity [17]. Naturally‐occurring DNA lesions tend to be isolated and homogeneously distributed and can thus be repaired efficiently by the DNA repair pathways. In contrast, clustered DNA damages such as those induced by ion particle irradiation have a reduced reparability compared to that of individual lesions [18].
1.2.1 The Non‐Homologous End Joining (NHEJ) Repair Pathway
Non‐Homologous End Joining (NHEJ) is the primary DSB repair pathway in the cell and rejoins DNA ends regardless of their homology, which increases the probability for genomic aberrations such as deletions, insertions and translocations [19]. Thus, NHEJ‐repair is an important DNA repair pathway which contributes to both genome protection and mutations. Classical NHEJ‐repair in mammalian cells was discovered in the 1980s when Mimori and colleagues first described the DNA end binding protein Ku [20]. However, it was not until 1994 when Stamato and colleagues revealed Ku’s function in the DDR by showing that cells lacking Ku are sensitive to irradiation [21]. Moreover, several groups observed that the repair of DSB in NHEJ‐deficient cells resulted in increased deletion frequencies and use of microhomologies at the repair junctions, which points to an additional NHEJ‐like DNA repair mechanism. This second pathway was called microhomology‐mediated end joining (MMEJ) or alternative NHEJ (aNHEJ), and occurs at approximately 10% of the frequency of normal or classical NHEJ (cNHEJ). Furthermore, it is less faithful than cNHEJ, since excessive deletions and chromosomal translocations are frequently found at the repaired DSB sites, with some of them leading to oncogenic transformation [22]. 5 INTRODUCTION
Both classical and alternative NHEJ‐repair can be divided into four basic steps: (1) DSB recognition, (2) end binding and synapsis formation, (3) end processing, and (4) ligation [22] (Figure 2). Classical NHEJ is initiated by binding of the Ku70/80 heterodimer to free DNA ends at the DSB site. Upon recognition of the DSB, the Ku heterodimer translocates along the DNA from the DSB site in order to allow additional Ku dimers to bind to the DNA, which protects the DNA termini from end resection and acts as a scaffold for the recruitment of additional repair factors including ATM, DNA‐PKcs and DNA polymerases. The Ser/Thr protein kinase ataxia‐telangiectasia mutated (ATM) is a key regulator of the DNA damage response and activates a plethora of downstream effectors by phosphorylation. Among its target molecules, 53BP1, H2AX, p53 and DNA‐PKcs are a few of the most intensively studied repair factors [23]. Another kinase, namely DNA‐PKcs (DNA‐dependent protein kinase, catalytic subunit) belongs to the same family as ATM and also phosphorylates several proteins such as H2AX, Artemis and XRCC4. Since these proteins are involved in downstream processes of DNA repair, their activation multiplies the DNA damage signal. In addition to activation of effector molecules for DNA repair, the DNA‐PK‐ Ku70/80 complex undergoes autophosphorylation, resulting in a conformational change that increases the accessibility of the DNA for additional DNA processing enzymes and ligases. Aligned and compatible DNA ends can be directly rejoined by the DNA ligase IV. However, complex DNA ends such as those produced by ionizing radiation require processing by additional enzymes to prepare the DNA termini for ligation. One of these processing enzymes is Artemis, which is directly activated by DNA‐PKcs. In complex with DNA‐PKcs, Artemis removes single‐stranded DNA (ssDNA) overhangs that contain damaged nucleotides. Then, XRCC4 interaction with the polynucleotide kinase/phosphatase (PNKP) results in the phosphorylation of 5’ OH DNA ends and the removal of the phosphate molecule from the 3’ DNA terminus, thereby forming compatible DNA ends for ligation. Subsequently, DNA polymerases fill in the gaps at the DSB site. In the final step of cNHEJ, the two DNA ends are rejoined by the XRCC4‐ligase IV‐XLF complex. XRCC4 stabilizes ligase IV and stimulates its ligation activity. XLF stimulates the ligation of non‐cohesive DNA ends, and is essential for gap filling by the DNA polymerases, suggesting that it plays an important role in the alignment of DNA ends and thus maintaining stability of the broken DNA ends. Upon repair of the DSB, the repair proteins dissociate or are removed from the DNA [22].
In contrast to cNHEJ, the mechanisms and proteins involved in alternative NHEJ remain poorly understood. A characteristic feature of aNHEJ is the use of a 0‐10bp microhomologous sequence during the alignment of the broken DNA ends. Furthermore, distinctive DNA repair signatures found at DSB sites repaired by aNHEJ imply that enzymes involved in aNHEJ promote end resection and include nucleases and ligases. Several proteins have been identified to be involved in end resection (Mre11, CtIP) and ligation (PARP1, DNA ligase III) [22] (Figure 2). 6 INTRODUCTION
Figure 2: Classical and alternative NHEJ‐repair in mammalian cells. During classical NHEJ‐repair, DSB are recognized by the Ku70/80 heterodimer, which recruits other repair factors. DNA‐PKcs multiplies the damage signal by phosphorylating several downstream targets such as Artemis, which processes the DNA ends for subsequent ligation by the XRCC4‐Ligase IV‐XLF complex. In contrast to cNHEJ, most repair factors involved in aNHEJ remain unknown. However, PARP1 is known to recognize the DNA break and Mre11 and CtIP are involved in end resection. Image modified from [22].
1.2.2 Methods for the detection of DNA damage and DNA repair activity
The most frequently used method for the detection of DSB and DNA repair activity is immunostaining of DNA repair proteins with fluorescently‐labeled antibodies and subsequent visualization by microscopy. Several DNA repair factors that assemble at the DSB site form large complexes that can be microscopically visualized. Among the most prominent molecules are DNA‐PK, 53BP1, and γH2AX. The histone variant H2AX is incorporated into the nucleosomes at DSB sites and becomes phosphorylated at its serine residue at position 139 (Ser139) by the kinase activity of DNA‐PK, ATM and ATR. Upon phosphorylation, γH2AX forms large foci, termed radiation‐ induced foci (RIF), which can span up to several megabases around the DSB site in order to facilitate DNA repair and recruit other DNA repair factors. When the DNA damage has been repaired, γH2AX is dephosphorylated and disassembles from the DSB site [2].
Another approach often used to study DNA repair sites and genomic aberrations is whole genome sequencing. In 2005, Roche/454 Life Sciences introduced the first commercially‐available next generation sequencing technology [24] that is capable of generating 80–120 Mb of sequence in 200‐ to 300‐bp reads. The process is divided into several sequential steps, starting with the isolation of genomic DNA, followed by a fragmentation step, the ligation of PCR adapters and separation into single DNA strands. The single‐stranded DNA fragments are subsequently captured on magnetic beads under conditions that favor one DNA fragment per bead. The beads are incorporated into oil droplets containing all PCR reagents that allow amplification, thereby producing millions of copies of a unique DNA template. Subsequently, the droplets are broken up, and each bead is deposit in a single picoliter‐sized fiberoptic well for pyrosequencing. Pyrosequencing is a sequencing‐by‐synthesis approach in which pyrophosphate (PPi) is released from the nucleotide by the DNA polymerase during nucleotide incorporation. The ATP sulfurylase converts the free PPi molecules into a substrate for the luciferase, which results in light emission and thereby determines the DNA sequence. Similar to the Roche/454 sequencing 7 INTRODUCTION
platform, Illumina sequencing is also a sequencing‐by‐synthesis approach. However, it does not require a pre‐ amplification step of the DNA template, since these are directly bound to the surface of a flow cell. The Illumina flow cell is densely populated with forward and reverse PCR primer adapters which are complementary to adapters ligated to the DNA templates. The DNA templates bind to the forward and reverse primer adapters of the flow cell and form a bridge that serves as the substrate for amplification. For sequencing, modified nucleotides with reversible terminators are used. This allows a single nucleotide to be incorporated in each sequencing cycle [25]. Thus, Illumina sequencing has a higher accuracy than the 454 platform. Each nucleotide carries its own chemically‐cleavable fluorescent dye at the 3’ OH terminus. The cleavage of the terminator results in fluorescence that is recorded by a camera. Recent advancement of the reversible‐terminator sequencing technology is the MiSeq sequencing by Illumina, which produces 2 x 300 paired‐end reads in a single run, allowing small genome sequencing and assembly. Further, it allows processing of more samples and generates more reads per run than previous Illumina sequencing platform [26].
1.3 Radio‐ and chemotherapy
1.3.1 Types of ionizing radiation
Ionizing radiation (IR) is defined as the radiation that has enough energy to remove electrons from atoms, and thereby ionizes them [27]. The IR energy is released inside the cell and is absorbed by various molecules such as proteins, lipids and the DNA and ionizes them. Radiation can be either directly or indirectly ionizing. During direct ionization, the radiation beam hits the target molecule in the cell and disrupts its structure. In contrast, during indirect ionization, the energy of the radiation beam is transferred to an electron of an atom, which is not part of the target molecule. This electron becomes excited, and, due to its higher energy, is lost from the atom. The ionized atom forms a radical that causes damage to different molecules inside the cell [7, 27] such as the DNA.
In general, two types of IR can be distinguished: photon and hadron. X‐rays and α‐rays belong to the group of photon radiation. X‐rays are generated by rapid stopping of highly accelerated electrons, have a wavelength between 0.01 and 10nm and energies in the range of 102 to 105 electron volt (eV). In contrast, hadron radiation consists of particles including protons, neutrons, and heavy charged ions such as carbon (12C) and ion (56Fe) atoms [7]. The two different types of radiation differ in their biological effectiveness which is expressed by the relative biological effect (RBE) value. The RBE is defined as the dose of a particular radiation divided by the dose of X‐rays required for an equal biological effect [27]. The higher the RBE for a specific radiation type, the more damage is induced per unit of energy deposited in the cell/tissue. In comparison to photons, carbon ions have an increased RBE, which is calculated between 2 and 5 depending on the cell type [28]. The different RBE of photons and hadrons result from the distances travelled by the IR in tissues and the pattern of ionizing events along the track. Photons are only sparsely ionizing, dispose their energy in atoms spaced by several hundred nanometers apart and cannot penetrate the tissue deeply. Thus, ionization events occur most at the tissue surface. In contrast, hadrons leave a dense trail of ionized atoms along their path that are spaced only about a tenth of a nanometer apart [29]. Moreover, hadron particles enter into the tissue deeply and only release small amounts of energy at the beginning of their route. At the end of their path, these particles rapidly decelerate and release high amounts of energy before stopping completely [30]. Since hadrons deposit their energy at a depth proportional to the energy of the charged particle [7], hadron irradiation allows a more precise deposition of energy inside the target tissue than photon irradiation. 8 INTRODUCTION
1.3.2 Radiation‐induced DNA damages
In order to determine the density of ionizations along the radiation track and thus the extent of radiation damage the Linear Energy Transfer (LET) is used as a measure. The LET is defined as the average energy deposition per unit length of the ionizing track, and its unit is keV/µm. Photons have a low LET, whereas in general hadrons have a high LET. Both low and high LET radiation induce a variety of DNA lesions including DSB, and the complexity of the DNA damage increases with increasing LET. Isolated DNA damages mainly occur after low LET irradiation, are spaced at a larger distance from other damages and can be repaired efficiently by the DNA repair machinery [29] (Figure 3).
High LET Low LET Excitation Ionization Radiation track Clustered DNA damage DNA damage
Isolated DNA lesions
Figure 3: Induction of ionizations and DNA damage by high‐ and low LET irradiation. High LET radiation causes more ionizations and excitations at high density than low LET radiation that creates more isolated DNA damages.
In contrast, high LET irradiation also induces complex clustered DNA lesions that include two or more lesions within 20bp or one helical turn (Figure 3). Amongst others, these DNA damages comprise abasic sites (AP), damaged bases and single‐strand breaks (SSB) that can be converted into potentially lethal DSB when the DNA repair is disrupted. Whether a non‐DSB cluster is converted into a complex DSB depends on the type of lesion induced, the distance separating the DNA lesions and whether the additional lesions disrupt the binding of DNA repair enzymes to other DNA damage sites [7]. Thus, in order to reduce the probability of DSB formation during damage repair, opposing DNA lesions are repaired sequentially [31]. Inefficient DNA repair of DNA damage clusters can result in increased levels of mutagenesis. The overexpression of certain DNA repair proteins such as the DNA glycosylase responsible for repair initiation can convert an oxidative DNA damage to a DSB (Figure 4). Non‐DSB clusters consisting of opposing AP sites are converted to DSB sites by the activity of the exonuclease Ape1, which stimulates cNHEJ‐repair or Ku‐independent DNA repair activity (Figure 4). Complex DNA damage clusters consisting of oxidized and abasic DNA molecules can be converted into a complex DSB by the nuclease ApeI, making it highly difficult for the cell to efficiently repair the damage [32]. Such complex clustered DNA damages are mainly induced by high LET radiation, are difficult to repair, have slow repair kinetics, and are thus considered to be more detrimental to the cell than randomly distributed DNA lesion induced by low LET radiation [33], thereby explaining the increase in RBE of high LET. In addition to the formation of complex clustered DNA lesions and radiation‐induced DSB, replication‐induced DSB sites are formed after ionizing radiation [34, 35], when a replication fork meets an unrepaired non‐DSB clustered damage site [35, 36]. 9 INTRODUCTION
Intact DNA
Oxidative damage cluster Abasic damage cluster Complex damage cluster O O A A AAA O
BER ApeI ApeI
O O A
BER DSB Complex DSB
Death NHEJ Death NHEJ Ku-independent (Ku, DNA-PK, (Ku, DNA-PK, DSB Repair XLF, XRCC4, XLF, XRCC4, HR, SSA, aNHEJ Repair efficient Ligase IV, Artemis) Ligase IV, Artemis)
Repair not always Repair efficient/accurate inefficient/mutagenic
Figure 4: Overview about repair of clustered DNA damages and repair outcomes. Two oxidative DNA damages (O) can be repaired efficiently by sequential base excision repair activity. However, replication through this damage can increase the mutation frequency of the base damage. Furthermore, in the presence of DNA glycosylases, two oxidative lesions can be converted into a DSB. Non‐DSB, abasic damage clusters are converted into DSB by the nuclease ApeI. DSB sites can induce cell death, or be repaired by error‐prone DSB repair pathways such as classical and alternative NHEJ. Complex DSB clusters resulting from high LET irradiation are more difficult to repair and can result in increased levels of mutagenesis or cell death. A: abasic site; O: oxidative damage; NHEJ: non‐homologous end joining; BER: base excision repair; HR Homologous Repair, SSA: Single‐Strand Annealing
1.3.3 The topoisomerase family
During transcription and replication, the DNA is locally unwound to allow the transcriptional and replication machinery to proceed. This, however, leads to DNA supercoiling and increased tension in adjacent genomic regions, stalling of the replication and transcription machinery as well as formation of abnormal DNA structures. Topoisomerases are enzymes involved in the unwinding of the DNA during transcription and replication. Upon replication, the replicated DNA strands are interlinked and need to be unlinked before cytokinesis can proceed. Failure to disentangle the two DNA strands can lead to genomic aberrations and induction of cell death. In order to protect the cell from replication‐induced damage, DNA topoisomerases also assist in the segregation of the daughter chromosomes before cell division [37].
The human genome encodes six topoisomerases, which are divided into type I and II. Type I topoisomerase (TOP1) only cleaves a single DNA strand, whereas the type II topoisomerase (TOP2) can induce DNA double strand breaks. Both types of topoisomerases cut the phosphodiester backbone of the DNA by a nucleophilic attack from the catalytic tyrosine at the catalytic center of topoisomerase. This reaction is reversible, and the DNA sequence remains unchanged upon religation. Mammalian cells have two TOP2 isoenzymes, namely α and β, which function as homodimers. The expression of TOP2α is closely linked to the cell cycle and the expression increases two‐ to three‐fold during G2/M phase. TOP2β on the other hand, is always expressed in both cycling and non‐cycling cells. The TOP2 isoenzymes have low sequence selectivity, but they preferentially recognize and bind DNA knots, supercoils and interlinks [37]. 10 INTRODUCTION
1.3.4 Topoisomerase 2 catalytic cycle and targeting by anticancer drugs
The TOP2 catalytic cycle is initiated by binding of the TOP2 homodimers to the gate (G) DNA segment, through which the transported (T) DNA segment is passed. After binding to the G segments, TOP2 binds the T DNA segment and two ATP molecules. Subsequently, the homodimer changes its conformation to a closed clamp form, called the TOP2 cleavable complex. Upon binding of Mg2+, the two tyrosyl residues of the TOP2 homodimers attack the phosphodiester backbone in the opposite DNA strands of the G segment to induce a DSB. In this stage, each of two topoisomerase monomers is covalently linked to the 5′‐terminus of an enzyme‐ generated DSB. Then, the T segment is rapidly passed through the G segment and released from the enzyme. After strand passage, the G segment is religated by TOP2, and ATP hydrolysis converts the closed clamp conformation of the enzyme to the open form to release the G segment [37] (Figure 5).
Doxorubicin Etoposide Doxorubicin
Figure 5: The TOP2 catalytic cycle (1) Upon recognition of a DNA crossover region, TOP2 binds to the DNA (G segment, green). (2) ATP binding leads to a conformational shift to a closed clamp form and binding of the T segment (purple). (3) The G segment is subsequently cleaved and (4) the T strand passes through the G segment. (5) TOP2 religates the G segment and (6) returns to its open conformation after ATP hydrolysis. At low concentrations (<1µM), doxorubicin acts like etoposide and inhibits TOP2 DNA religation, whereas at concentrations above 10µM doxorubicin intercalates into the DNA, thereby blocking TOP2 binding. Figure modified from [38].
Since failure to disentangle two interlinked DNA strands can lead to the induction of cell death, TOP2 enzymes are frequently targeted in cancer chemotherapy. Generally, anti‐cancer drugs targeting TOP2 can be classified according to their mechanisms. Molecules that inhibit the religation of the G segment such as etoposide and doxorubicin are termed TOP2 poisons, whereas TOP2 inhibitors such as genistein and azatoxins enhance the formation of the TOP2 cleavable complex. In addition to stimulating DSB formation, TOP2 poisons and inhibitors also induce SSB, affect nuclear processes such as transcription and replication by intercalating into the DNA and by generating reactive oxygen species (ROS). Doxorubicin belongs to the family of anthracyclines, and, at high concentrations (10μM), intercalates into the DNA, which alters the DNA structure and prevents TOP2 from 11 INTRODUCTION
binding to the DNA. At concentrations below 1µM, doxorubicin acts like etoposide and stabilizes the cleavable complex, thereby prolonging the half‐life of the TOP2‐DNA‐intermediate and increasing the possibility of DSB formation. In order for DSB repair to occur, the covalently attached TOP2 enzyme is removed by cellular end‐ processing enzymes. The DNA fragment linked to the peptide is excised by nucleases such as the MRN complex, CtIP or Artemis, and the DSB is repaired by NHEJ [39‐41].
1.3.5 Cancer therapy‐induced delayed genomic instability
In progenitors of radiation‐surviving cells, genomic changes can arise several generations of the initial DNA insult. This phenomenon is known as delayed radiation‐induced genomic instability, and is characterized by the expression of several radiation‐induced effects including apoptosis, gross chromosomal rearrangements, aneuploidy as well as gene mutations and amplification [31]. The mechanisms that initiate and drive delayed genomic instability in progenitor cells are not fully understood yet. However, experimental evidence suggests that increased levels of oxidative stress contribute to radiation‐induced genomic instability, since cells with mitochondrial dysfunction and cells exposed to hydrogen peroxide initiate delayed instability, and treatment with antioxidants can greatly reduce these effects [42, 43]. Moreover, it also possible that delayed genomic instability is caused by delayed DSB induction and subsequent misrepair by NHEJ. Delayed DSB induction and illegitimate joining of DNA ends can generate dicentric chromosomes which block segregation during mitosis, thereby inducing additional DSB and accumulation of mutations [44]. Since radiation‐induced genomic instability is transmitted through the genome for several generations, it was speculated that the initial ionization event is memorized in the genome [45]. Several studies now suggest that radiation induces alterations in local chromatin structures that can lead to increased levels of replication stress and DSB that can initiate genomic instability in radiation surviving cell populations [44, 45]. Despite these results, the functional consequences of delayed genomic instability on carcinogensis and radiosensitivity have not been described to date [44]. Nonetheless, since the genomic effects of delayed genomic instability are similar to those induced directly by irradiation, it is assumed that these genomic changes initiate or drive carcinogenesis [46‐48]. Delayed induced genomic instability has mostly been observed and studied in radiation surviving cells, but, persistent destabilization of the genome following chemical treatment was also reported. For example, bleomycin and neocarzinostatin were equally efficient in inducing delayed genomic instability in progenitors of chemotherapy‐surviving cells [49]. Moreover, anti‐topoisomerase drugs have been reported to induce structural and numerical chromosome aberrations in surviving cells [50]. Thus, both irradiation and chemotherapy can induce delayed genomic instability, which potentially leads to cancer‐therapy resistance and therapy‐induced carcinogenesis.
1.4 Lentiviruses
1.4.1 History and phylogeny of lentiviruses
In 1911, Peyton Rous showed that cancer could be transferred from chicken suffering from sarcoma to healthy chicken by using an ultra filter extracts [51]. Later, it was discovered that viruses in the extract were the cancer‐ inducing agent, and this virus was named after its discoverer Rous Sarcoma Virus (RSV). In 1970, Howard Temin, Satoshi Mizutani and David Baltimore discovered the enzyme reverse transcriptase in RSV, which enables retroviruses to convert their single‐stranded RNA genome into double‐stranded DNA [52, 53]. In the following years, another characteristic feature of retroviruses, the integration of the proviral genome into the host cell’s 12 INTRODUCTION
genome was discovered [54], which is mediated by the viral integrase enzyme. In the following decade, the first human oncogenic retrovirus (HTLV) [55] and the immunodeficiency causing virus HIV [56] were discovered. These viruses belong to the retroviridae family which is divided into two subfamilies: orthoretroviridae and spumaretroviridae. The subfamily orthoretroviridae further consists of six genera (alpharetrovirus, betaretrovirus, gammaretrovirus, deltaretrovirus, epsilonretrovirus, lentivirus) whereas the spumaretroviridae only has one genus (spumavirus) [57]. Each genus is further subdivided into different types of subspecies. Lentiviruses belong to the subfamily orthoretroviridae and are single‐stranded, positive‐sense RNA viruses that have a diploid genome with a length of 7‐12kb. The virions are enveloped and 80‐100nm in diameter. Moreover, these viruses are characterized by two viral enzymes: reverse transcriptase and integrase, which convert the RNA genome into double‐stranded DNA and integrate it into the host cell genome. Another characteristic of lentiviruses is their ability to infect both dividing and non‐dividing cells. Infection with lentiviruses can result in different diseases such as immunodeficiencies, anemia and encephalitis [58]. Since in this dissertation a HIV‐1‐ derived lentiviral vector was used, further descriptions are based on the HIV‐1 genome.
1.4.2 The lentiviral genome
The lentiviral genome exists as two single‐stranded positive‐strand RNA molecules and has a 5’ cap structure and a 3’ polyadenylation. The proviral genome is flanked by two, 640bp long terminal repeats (LTR) that are required for transcription, reverse transcription and integration into the host cell genome. Each LTR is made of a U3, R and U5 region and contains several promoter and enhancer elements. The lentiviral genome further contains a primer binding site (PBS) necessary for binding of a tRNA that initiates the reverse transcription of the RNA genome. Located in 3’ to the PBS is the packaging and dimerization signal psi (Ψ), which mediates packaging of the RNA genome during virion assembly. At the 3’ LTR, the polypurin tract (3’PPT) required for the synthesis of the second DNA strand during reverse transcription is encoded. The viral core proteins, enzymatic proteins, and the envelope glycoproteins shared by all retroviruses are encoded in the gag, pol and env gene. Complex retroviruses, such as lentiviruses, also contain six additional genes (tat, rev, vif, vpr, vpu, and nef) important for HIV infection and pathogenicity, making it a total of nine open reading frames (Figure 6) [58]. 13 INTRODUCTION
A HIV RNA Genome
PBS cPPT RRE 3’PPT
RU5 Ψ U3 R Reverse Transcription
B Viral DNA Genome nef tat
gag vif rev LTR LTR
U3 RU5 pol vpr env U3 RU5 vpu
Figure 6: The RNA and proviral genome of HIV‐1. (A) Structure of the RNA genome. The 5’ and 3’ end are modified, carrying a cap structure and a polyadenylation, respectively (not shown). At the primer binding site (PBS) a tRNA for the initiation of reverse transcription is bound (not shown). Psi (Ψ) is the packaging signal, U3, R and U5 mark the end of the HIV genome and form the long terminal repeats (LTR) after reverse transcription. The central polypurine tract (cPPT) is important for transportation of the provirus into the nucleus. (B) Schematic of the proviral genome. During reverse transcription, the U3 region at the 3’ end is copied to the 5’ end and the 5’ U5 region to the 3’ end to form the long terminal repeats. The location of the nine lentiviral genes is shown.
The gag gene encodes four viral capsid proteins that are derived from a single precursor Gag protein called p55 and that are necessary for the formation and release of viral particles. For lentiviral replication, the viral protease, reverse transcriptase and the integrase are required, which are encoded in the pol gene. The gag and pol genes are synthesized from the same mRNA transcript by a ribosome frameshifting near the 3’ end of the gag gene. The resulting Gag‐Pol precursor protein is processed by the viral protease inside the virions. The env gene encodes the viral surface protein gp120 and transmembrane gp41 protein. Similar to the Gag and Pol proteins, these mature proteins are processed from a single precursor protein, gp160, by proteolytic activity. The Gag, Pol and Env proteins are essential for the formation of mature virions and the infection of target cells. One of the accessory proteins encoded in the genome of lentiviruses is the transactivator Tat, which binds to the Tat response element (TAR) located in the LTR and plays a critical role for the transactivation and transcription of proviral DNA as well as the lentiviral replication. Besides, the Rev protein promotes the nuclear export of lentiviral RNA by binding specifically to the Rev response element (RRE) located in the env region, thereby increasing the half‐life of viral mRNAs. Both Tat and Rev are translated from early transcribed mRNA [58].
1.4.3 The life cycle of lentiviruses
The life cycle of lentiviruses is divided into early and late stages. In the early stages, virus entry, reverse transcription of the RNA genome and integration into the genome occur. The late stages of the lentiviral life cycle are characterized by the transcription of the integrated viral genome, translation of viral transcripts into proteins required for viral assembly and budding from the host cell (Figure 7). 14 INTRODUCTION
The lentiviral life cycle begins with the recognition and binding of the viral surface protein Gp120 to its primary receptor CD4 and the co‐receptor CXCR4 on T‐lymphocytes or CCR5 on macrophages and dendritic cells. Binding initiates a conformational change in the viral transmembrane protein Gp41 required for the fusion of the viral membrane with the cell membrane. Upon viral entry into the cell, the capsid proteins are uncoated, and the lentiviral genome, reverse transcriptase, protease and integrase are released into the cytoplasm. Subsequently, the RNA genome is converted into the complementary double‐stranded DNA by the enzymatic activity of the reverse transcriptase [58]. The viral enzyme integrase (IN) specifically binds to the U3 region in the 5’ LTR and the U5 region in the 3’LTR of the proviral cDNA. IN removes nucleotides from the 3’ ends of the viral DNA beyond a conserved ‘CA’ dinucleotide, thereby creating two single‐stranded 5’ overhangs. The processed proviral DNA is subsequently imported into the nucleus, where the cellular DNA is cleaved by IN, the 5’ dinucleotide overhang in the viral DNA is removed and the 3’ DNA ends joined to the 5’ ends of the genome [59]. Following stable integration, the host cell transcriptional machinery is hijacked to transcribe the provirus. The 5’ LTR has basal promoter activity that is sufficient to initiate transcription by cellular RNA polymerase II. The first mRNA transcripts are multi‐spliced mRNAs that are exported from the nucleus into the cytoplasm where they are translated into Rev, Tat and Nef proteins, required for the initiation of subsequent events in viral transcription. The Tat protein binds to the TAR element at the 5’ end of viral mRNAs, leading to the transactivation and transcription of other genes from the viral DNA. In addition to the Tat protein, the Rev protein binds to the Rev‐responsive element on viral mRNA transcripts and removes them from the splicosome, which leads to the export of singly‐spliced and unspliced mRNA and viral genomes into the cytoplasm. Singly‐ spliced mRNAs are translated at the ribosomes into the proteins Env, Vif, Vpr, and Vpn, whereas unspliced mRNA are translated into the Gag‐Pol precursor protein. Following transcription and translation, the viral proteins and the genomic RNA assemble at the cell membrane, where viral Env proteins are integrated into the cell membrane. The unspliced RNA genome copies are then packaged into the virions and released from the cell. Subsequently, the multimerization of Gag and Gag‐Pol precursor proteins activates the viral protease, converting immature to mature HIV virions (Figure 7) [58]. 15 INTRODUCTION
Figure 7: Lentiviral life cycle. In the early stage of viral infection, the virus attaches to the target cell and fuses with the cellular membrane to release the capsid into the cell. The capsid is subsequently uncoated, the RNA genome reverse transcribed, imported into the nucleus and integrated into the genome. After integration, the lentiviral genes are transcribed and exported into the cytoplasm. The viral mRNA is translated, and the lentiviral RNA genome and the proteins assemble into virions at the cell membrane. NPC: nuclear pore complex. Image taken from [60]
The integration profile of HIV in the genome of their host cells is non‐random. HIV preferentially integrates into genomic regions with a high gene density and particularly into coding sequences. However, integration upstream of the transcription start site is not favored [61, 62]. Furthermore, HIV integration is influenced by the transcriptional activity: the integration frequency into transcriptionally active genes is increased [63], but genes with high transcriptional activity are less favored [61]. Regions rich in the dinucleotide CpG, termed CpG islands, commonly correspond to gene regulatory regions that frequently contain promoter and enhancers. For HIV, these regions and their surroundings are disfavored [61]. Hence, gene‐dense and transcriptionally‐active genomic regions, but not CpG islands are preferred sites of HIV integration.
1.4.4 Structure of lentiviral vectors for gene therapy
Because of their ability to infect both dividing and non‐dividing cells as well as stably integrate into the genome, lentiviruses are used as vehicles to introduce transgenes into target cells for more than 20 years [58]. In order to generate replication‐incompetent viruses for gene transfer, the lentiviral genome sequence was modified. Today, plasmid vector systems are used in which all elements required for production of functional virions (trans‐acting factors) of the viral genome are divided onto four plasmids to reduce the likelihood of recombination and formation of replication‐competent viruses. In principal, the first plasmid encodes the packaging genes gag and pol. In the second plasmid, the rev gene that is required during lentiviral transcription 16 INTRODUCTION
is encoded. On the third plasmid, the Env protein is often replaced by the VSV‐G protein (vesicular stomatitis virus ‐ protein G) to increase the tropism of the lentivirus. In order to prevent that the three plasmids containing the trans‐acting factors are packaged into mature virions and that replication‐competent viruses form, the packaging signal psi and the LTR sequences have been cloned into a fourth plasmid, called the transfer vector. This vector is packaged into the virions, and contains the sequence for reverse transcription and the transgene. Moreover, to further reduce the likelihood of recombinations, the U3 region in the LTR containing the promoter and enhancer elements is truncated [64]. Furthermore, the requirement of lentiviral replication for the Tat protein was eliminated, by replacing the U3 region in the 5’ LTR with a constitutively active promoter from the cytomegalovirus (CMV) or RSV. Vectors with these LTR modifications are called self‐inactivating (SIN), because they lack LTR promoter activity following integration, thereby reducing the likelihood of transcription activation of proto‐oncogenes located in vicinity to the lentiviral integration site. Moreover, increased transduction efficiency and transgene expression in vitro and in vivo was achieved by placing a central polypurine tract (cPPT) sequence downstream of the RRE in the transfer vector. Another genetic element in the transfer vector is the posttranscriptional regulatory element WPRE (woodchuck hepatitis virus post‐transcriptional element), which increases the amount of transgenic mRNA. For production of functional viral particles, the four plasmids are co‐ transfected into a packaging cell line in which the genomic information is transcribed and translated into mature viral particles, containing the transfer vector.
In addition to integration‐competent lentiviruses, episomal‐remaining, non‐integrating lentiviral vectors have been developed, which enable transient transgene expression in infected cells. These lentiviruses are termed integrase‐deficient lentiviruses (IDLV) and are generated by introducing a point mutation at the catalytic core of the integrase gene that changes the amino acid at position 64 from aspartic acid to valine (D64V). This modification was shown to inhibit integration by up to four logs compared to integrase‐competent lentiviruses [65, 66], and several studies suggest that the few observed integration events are mediated by cellular DNA repair mechanisms [65]. Indeed, integrated IDLVs showed a high frequency of LTR deletions, a key signature of NHEJ‐repair activity, and occurred at sites of DNA damage and repair. Additionally, blocking ATM, a key player in DNA repair, also prevented integration of IDLV at DSB sites [67].
1.5 Scientific aims
Current methods for DSB detection have several limitations, which hamper the analysis of induced and repaired DSB as well as genomic instabilities in irradiated cells: 1) Immunostaining of DNA repair proteins is an indirect detection method that does not enable the identification of DSB sites at single‐nucleotide resolution, 2) DNA repair proteins form microscopically‐visible foci which disassemble upon DNA repair and do not allow DSB site analysis in surviving cell populations, 3) Immunostaining does not give any information on the relationship between DSB locations, DNA repair pathway choice and cell fate decision. Even though the high‐throughput sequencing platforms are frequently used to study the mutational spectra in various cancer types [68], the high costs for sequencing large numbers of whole genomes and the analysis of sequencing data from heterogeneous cell populations make this method impractical for the identification of low frequency genomic events. Moreover, it does not provide any information, whether the identified mutation has functional consequences on cell survival and therapy resistance. Hence, there is little information on how radiation‐induced and repaired DSB sites are distributed, how radiation‐induced DNA damage is being survived and how these damages induce radioresistance and cell transformation. Analyzing the genomic distribution of radiation‐induced DSB in irradiated and expanded cells at single‐nucleotide resolution will help to improve our understanding of the 17 INTRODUCTION
mechanisms of radiation‐induced genomic instability and radiation resistance. In this thesis, a new methodology to capture induced and repaired DSB sites in radiation‐surviving cell populations has been used to study DSB site distribution. Target cells become transduced with an integrase‐deficient lentivirus (IDLV) that carries a point mutation in its integrase gene, preventing integrase‐mediated integration of the proviral DNA into the host genome of the cell. Upon DSB induction by irradiation, these IDLV DNA molecules serve as molecular tags, which become stably integrated into the genome by the cellular NHEJ‐repair activity, thereby marking the DSB site in vivo. The integration of IDLV at induced and repaired DSB sites can be followed by PGK promoter‐driven EGFP expression from integrated IDLV by flow cytometry. The DSB repair sites can be amplified and identified using LAM‐PCR and deep sequencing (Figure 8).
IR/Dox IR/Dox IR/Dox
Genomic DNA DSB DSB DSB Induced DSB IDLV NHEJ Repair of DSB
NHEJ
LTR IDLV-PGK-eGFP LTR IDLV “DSB trapping”
5’LAM-PCR 3’LAM-PCR Amplification of DSB by LAM-PCR
GTACCTGTTCA TCTGGAAGCTATTT Localization of DSB at Sequencing of DSB Loci single nucleotide resolution
Figure 8: Proposed mechanism of IDLV‐based DSB capturing. The double‐stranded DNA bait delivered into cells by IDLV is captured by the cellular NHEJ‐repair machinery at DSB sites. This leaves a stable genetic tag which enables the mapping and tracking of radiation (IR)‐ or doxorubicin (Dox)‐induced and repaired DSB in the genome of treated cells. The frequency of DSB tagging can be followed by PGK promoter‐driven EGFP expression during expansion. Localization of captured DSB is performed by amplifying the vector‐genome junction using 5’ and 3’ LAM‐PCR and deep sequencing. DSB: DNA double‐strand breaks, IR: irradiation; Dox: doxorubicin; IDLV: integrase‐deficient lentivirus; NHEJ: Non‐Homologous End Joining, eGFP: enhanced green fluorescent protein; PGK: Phosphoglycerate Kinase 1 promoter; LTR: Long terminal repeat
The following scientific aims were addressed:
1. Can radiation‐induced DSB be stably marked, tracked and identified at single‐nucleotide resolution during expansion? 2. How do transcriptional and epigenetic states influence DSB site distribution? 3. Do frequently damaged and repaired genomic regions exist that are likely to influence radiation‐ induced genomic instability and radiotherapy?
The obtained results from this work should bring new insights into the mechanisms that initiate DSB‐induced genomic instability, radiotherapy resistance and carcinogenesis.
18 MATERIALS AND METHODS
2. MATERIALS AND METHODS
2.1 Materials
2.1.1 Chemicals
Chemicals/Reagents Company 100 bp / 1 kb Marker Invitrogen Agarose LE Sigma Ampicillin Roth
Aqua ad iniectabilia (dH2O) Braun BD™ Cytometer Setup & Tracking Beads Kit BD Beckton Dickinson BD FACS Clean Solution BD Beckton Dickinson BD FACS Flow Sheath Fluid BD Beckton Dickinson BD FACS Rinse Solution BD Beckton Dickinson Bovine Serum Albumine (BSA) Sigma Bromphenol blue Sigma Deoxyribonucleotic triphosphate (dNTP) Fermentas (Thermo Fisher Scientific) Dimethylformamid Sigma Dulbecco's Modified Eagle Medium (DMEM) Invitrogen Ethanol VWR Ethidiumbromid solution (0.07%) Applichem Ethylenediaminetetraacetic acid (EDTA) Applichem Fetal Calf Serum (FCS) PAN Glycerol Sigma‐Aldrich Guanidin hydrochloride Sigma Hexanucleotid Mix (10x) Roche Human genomic DNA Roche Iscove's Modified Dulbecco's Medium (IMDM) Invitrogen Isopropanol Sigma‐Aldrich LB Agar Miller US Biological Lithiumchlorid (LiCl) Sigma Loading Buffer (5x) Elchrom Scientific Luria‐Bertani Broth (LB) Invitrogen
Magnesiumchlorid (MgCl2) Sigma ms2RNA Roche Sodium hydroxid (NaOH) Fluka Dynabeads M‐280 Streptavidin Dynal Dynabeads MyOne Streptavidin T1 Dynal PCR Grade Water Roche Penicillin/Streptomycin (Pen/Strep) Invitrogen Dulbecco’s Phosphate Buffered Saline (DPBS; pH 7,4) Gibco Polybrene (1000x; 8 µg/ml) Sigma Polyethylenimin (PEI; 1mg/ml) Sigma‐Aldrich Propidium iodide (1mg/ml) Molecular Probes (Invitrogen) Proteinase K Roche/Qiagen Puromycin Invitrogen
RNase/DNase free H2O Ambion Tris‐borate‐EDTA (TBE) Buffer (10x) Amresco Trizma‐HCl (Tris‐HCl) Applichem 19 MATERIALS AND METHODS
Trypanblue Invitrogen Trypsin/EDTA (0,05%) Life Technologies Tween 20 Sigma Vectashield Mounting Medium with DAPI Vector Laboratories X‐Gal Sigma
2.1.2 Enzymes
Enzymes Company CircLigase ssDNA ligase Epicentre Klenow DNA Polymerase Roche Quick DNA ligase Epicentre T4 DNA Ligase New England Biolabs Restriction enzymes with respective buffers New England Biolabs SYBRGREEN I Mix Roche Taq DNA Polymerase Qiagen/Genaxxon
2.1.3 Bacteria
Bacterial Strain Genotype Company E.coli TOP10 F‐ mcrA Δ(mrr‐hsdRMS‐mcrBC) Φ80lacZ ΔM15 Life Technologies ΔlacX74 recA1 araD139 Δ(ara leu) 7697 galU galK rpsL (StrR) endA1 nupG ‐ ‐ E.coli Stbl3 F mcrB, mrr‐hsdS20 (rB , mB‐), recA13, supE44 Life Technologies ara‐14, galK2, lacY1, proA2, rpsL20(StrR), xyl‐5 λ‐leumtl‐1
2.1.4 Cell lines and primary cells
Name Description Company A549 Human alveolar adenocarcinoma cell line [69] ATCC HEK 293T Human embryonic kidney cell line, stably ATCC expressing the SV40 T‐antigen [70] Hela Human epithelial carcinoma cell line ATCC NHDF‐A Adult normal human dermal fibroblasts PromoCell PC3 Human prostate cancer cell line [71] ATCC U87 Human glioblastoma cell line [72] ATCC
20 MATERIALS AND METHODS
2.1.5 Antibodies
Name Description Company Alexa Fluor® 647 anti‐ anti H2AX‐specific antibody labeled Biolegend H2A.X‐Phosphorylated with Alexa Fluor 647 (Ser139) Antibody (250ng/ml) Alexa Fluor® 647 Mouse Isotype control antibody, Antibody Biolegend IgG1, κ Isotype Ctrl (ICFC) labeled with Alexa Fluor 647
2.1.6 Plasmids
Name Description Lentiviral transfer vector expressing EGFP under control of pCCLsincPPT.PGK‐IRES‐eGFP.WPRE (LV106) human PGK promoter Plasmid encoding gag/pol genes and carries D64V mutation in LV001 integrase gene LV102 env‐encoding plasmid LV103 Plasmid encoding the VSV‐G protein #1211 Plasmid encoding CCR5‐specific ZFN monomer 1 #1212 Plasmid encoding CCR5‐specific ZFN monomer 2 pUC‐derived subcloning vector with multiple cloning site, pCR2.1 TOPO‐TA ampicillin and kanamycin resistance cassette
2.1.7 Oligonucleotides
DNA oligonucleotides were partially biotinylated (B) at the 5‘ terminus. Additional modifications include dideoxycytosine (ddC) to inhibit ligation of DNA oligos to 3’ terminus and phosphothiorate (*) in the phosphate backbone of the last three bases of some DNA oligos. Oligonucleotides were cleaned up by high performance liquid chromatography (HPLC) and lyophilized. Oligonucleotides were purchased from MWG or Sigma Aldrich. B,
Biotin; D: degenerated base; LC, Linker cassette; Tit, Titanium 454 primer; (N)2‐6, Recognition sequence for pyrosequencing.
2.1.7.1 Standard primers for q‐RT‐PCR
Name Sequence (5´‐3´) Myo461‐439 CTCCCAGTGGCACAGCAGTTAGG Myo122‐143 TGTGCCCCAGGTTTCTCATTTG GFP2 fwd TGAGCAAGGGCGAGGAGCTGTT GFP3 rev GCCGGTGGTGCAGATGAACT
21 MATERIALS AND METHODS
2.1.7.2 Primers used for linker cassettes in LAM‐PCR
Name Sequence (5´‐3´) LC1 GACCCGGGAGATCTGAATTCAGTGGCACAGCAGTTAGG LC1 (CATG) GACCCGGGAGATCTGAATTCAGTGGCACAGCAGTTAGGCATG LC3 (CG) CGCCTAACTGCTGTGCCACTGAATTCAGATC LC2 CCTAACTGCTGTGCCACTGAATTCAGATC LC3 (AATT) AATTCCTAACTGCTGTGCCACTGAATTCAGATC LC3 (TA) TACCTAACTGCTGTGCCACTGAATTCAGATC
2.1.7.3 Primers used for LAM‐PCR
Name Sequence (5´‐3´) SK‐LTR 1bio B ‐GAGCTCTCTGGCTAACTAGG SK‐LTR 3bio B ‐GAACCCACTGCTTAAGCCTCA SK‐LTR 4bio B ‐AGCTTGCCTTGAGTGCTTCA SK‐LTR 5 AGTAGTGTGTGCCCGTCTGT SK‐LTR 5 1/2 GTGTGACTCTGGTAACTAGAG LCI GACCCGGGAGATCTGAATTC LCII GATCTGAATTCAGTGGCACAG
2.1.7.4 Fusionprimer for Pyrosequencing
Name Sequence (5´‐3´)
Tit3nrLV CCATCTCATCCCTGCGTGTCTCCGACTCAG(N)6‐10 GATCCCTCAGACCCTTTTAGTC Tit3SKLV CCATCTCATCCCTGCGTGTCTCCGACTCAG(N)6‐10 TGTGTGACTCTGGTAACTAG
Tit5SKLV CCATCTCATCCCTGCGTGTCTCCGACTCAG(N)6‐10 AAGCAGATCTTGTCTTCG
MegaL6/10T GCCTCCCTCGCGCCATCAG(N)6‐10GATCCCTCAGACCCTTTTAGTC
MegaL_U3_10/T GCCTCCCTCGCGCCATCAG(N)6‐10AAGCAGATCTTGTCTTCG MiS3nrLV AATGATACGGCGACCACCGAGATCTACACTCTTTCCCTACACGACGCTCTTCCGATCT
(N)6‐10GATCCCTCAGACCCTTTTAGTC AATGATACGGCGACCACCGAGATCTACACTCTTTCCCTACACGACGCTCTTCCGATCT Mis3SKLV (N)6‐10TGTGTGACTCTGGTAACTAG Tit Linker B‐CCTATCCCCTGTGTGCCTTGGCAGTCTCAGAGTGGCACAGCAGTTAGG Megalinker B‐GCCTTGCCAGCCCGCTCAGAGTGGCACAGCAGTTAGG
MiS_LK GACCCGGGAGATCTGAATTCAGTGGCACAGCAGTTAGG(N)16CTA
22 MATERIALS AND METHODS
2.1.7.5 Primers and oligos used for direct DSB labeling approaches
Name Sequence (5´‐3´) L.CDSB 1 B‐CCTTGGGAGGGTCTCCTCTGAGTGATTGACAAAAAD L.CDSB 2 B‐CTTGGGAGGGTCTCCTCTGAGTGATTGACAAAAA L.CDSB 2‐1 CTTGGGAGGGTCTCCTCTGAGTGATTGACAAAAA E.CDSB 3 CTTGGGAGGGTCTCCTCTG P‐GTAGTCAATACATCAGAGGAGACCAGTCGGATGCAACTGCAAGATATTG dsGRUV1 GATACACGGGTACC*C*G*G P‐GTAGTCAATACATCAGAGGAGACCAGTCGGATGCAACTGCAAGATATTG dsGRUV2 GATACACGGGTACCCGGGACCCG*G*G*A P‐CCGGGTACCCGTGTATCCAATATCTTGCAGTTGCATCCGACTGGTCTCCT dsGRUVrev CTGATGTATTGA*C*T*A‐ddC P‐GTAGTCAATACATCAGAGGAGACCAGTCGGATGCAACTGCAAGATATTG ssGRUV5‐A‐Phthio GATACACGGGTACC*C*G*G‐ddC GRUV5‐2expo CATCCGACTGGTCTCCTCTGATG
2.1.8 Commercial kits
Kits Company Ampure XP beads Beckman Coulter Fast‐Link Ligation Kit Epicentre Fluorescence Biotin Quantitation Kit ThermoScientific High Pure PCR Template Preparation Kit Roche HiSpeed Plasmid Purification Kit Qiagen Microcon‐30 Kit Millipore QIAamp DNA Mini Kit Qiagen QIAfilter Plasmid Purification Kit Qiagen QIAprep Spin Miniprep Kit Qiagen QIAprep Spin Maxiprep Kit Qiagen QIAquick PCR Purification Kit Qiagen QIAquick Gel Extraction Kit Qiagen TOPO‐TA Cloning Kit Invitrogen
23 MATERIALS AND METHODS
2.1.9 Buffers, Media, Solutions
Buffers, Media, Solutions Chemical Final Concentration 3M LiCl Solution** Tris‐HCl (pH 7.5) 10 mM EDTA 1 mM LiCl 3 M 6M LiCl Solution** Tris‐HCl (pH 7.5) 10 mM EDTA 1 mM LiCl 6 M Acid‐isopropanol solution HCl (1N) 0.04N Isopropanol Ampicillin** Ampicillin sodium salt 100mg/ml Desalted water Cell culture freezing medium DMSO 15% FCS 30% Cell culture medium 55% Denaturation solution NaOH 0.1 M DMEM Cell culture medium DMEM 89% FCS 10% Pen/Strep 1% DNA loading buffer (5x) Tris‐HCl (pH 7) 25 mM EDTA (pH 8) 150 mM Bromphenol blue 0.05% Glycerol 25% DPBS‐Tween 20 (DPBST) Tween 20 0.2% DPBS (pH 7.4) IMDM cell culture medium IMDM FCS 10% Pen/Strep 1% LB‐Agar* LB‐Miller Agar 3.7% Desalted water
LB‐medium* LB 2% Desalted water MTT stock solution** MTT 5mg/ml 1xDPBS Paraformaldehyde solution** Paraformaldehyde 4% DPBS (pH 7.4) Triton solution Triton X‐100 0.5% DPBS (pH 7.4) Washing solution for paramagnetic beads** DPBS (pH 7.4) BSA 0.10% X‐Gal X‐Gal 20 mg/ml Dimethylformamid * Autoclaved and addition of antibiotics (Ampicillin, Kanamycin) after cooling to 60°C.
** Solutions were sterilized by filtering through 0.22µm filter
24 MATERIALS AND METHODS
2.1.10 Disposables
Disposable Company Sheeting VWR Sheeting for LightCycler LC480 Roche Polypropylene Round Bottom Tube (15 ml) BD Beckton Dickinson Polystyrene Round Bottom Tube (5 ml) BD Beckton Dickinson Lid for 96‐well plates Greiner bio‐one Falcon, BD™ Falcon™ Tubes (15 ml, 50 ml) BD Beckton Dickinson Filter (0,22 µm, 500 ml) Millipore Filter System (0,22 μm) Stericup® Millipore Gloves (Nitril) Microflex Ionoculation Loop Sarstedt Parafilm Brand PCR‐Tubes Softtubes (0,2 ml) Kisker Biotech Pipette tips Starlab Pipette tips for LightCycler LC480 Starlab Mixing plates (96‐well) Greiner bio‐one Plates for LAM‐PCR (96‐well) Greiner bio‐one Plates for LightCycler LC480 (96‐well) Roche Photobase paper VM 65 H Mitsubishi Reaction tubes (0,5 ml, 1,5 ml, 2 ml) Eppendorf RNase/DNase‐free reaction tubes Ambion (0,5 ml, 1,5 ml, 2 ml) Ultracentrifugation tube Beckman Coulter Cell culture flasks (25 cm2, 75 cm2, 225 cm2) Nunc Brand Products Cell culture pipettes (2‐50 ml) BD Beckton Dickinson Cell culture plates (6‐, 12‐, 24‐, 96‐well) BD Beckton Dickinson Cell culture dish (10 cm, 15 cm) Greiner bio‐one Cell scraper BD Beckton Dickinson Cryotube BD Beckton Dickinson
2.1.11 Equipment
Equipment Company Autoclave Systec BDTM LSRII Flow cytometer BD Beckton Dickinson Cell culture hood Heraeus Centrifuges Eppendorf Lysine‐coated coverslips BD Beckton Dickinson Electrophoresis Power Supply Pharmacia/Elchrom Scientific Fluorescence microscope Carl Zeiss Jena Freezer ‐20°C Liebherr Freezer ‐80°C Sanyo Fridge Liebherr Gel documentation system Peqlab Gel electrophoresis chamber Biometra 25 MATERIALS AND METHODS
Heating Block Eppendorf Horizontal shaker (KS 250B) IKA Labortechnik Incubator (37°C) Binder Lifesciences Ice machine Ziegra Infinite 200” plate reader Tecan LightCycler LC480 Roche Liquid Nitrogen Tank Thaylor‐Wharton Magnetic Particle Collector MPC 96 Dynal Microplate reader Biotek Microscope Carl Zeiss Jena Microwave Siemens Multi‐channel pipette Eppendorf NanoDrop spectrophotometer Thermo Scientific Neubauer counting chamber Optik Labor OptimaTM L‐90K Ultrazentrifuge Beckman Coulter PCR cycler Biometra Picofuge NeoLab Pipettes (Pipetman P2, P10, P200, P1000) Eppendorf Pipette device Integra Bioscience Pipetboy acu Proton and Carbon Radiation Source Heidelberg Ion Therapy Center Scales Sartorius Special accuracy weighing machine Sartorius Vacuum pump NeoLab Videoprinter Mitsubishi Vortexer (MS1) IKA Labortechnik Water bath Thermo Electron Coporation XRAD320 X‐ray device Precision X‐Ray
2.1.12 Software and data bases
Software and data bases Company Adobe Acrobat X Pro Adobe BLAST Search http://www.ncbi.nlm.nih.gov/blast BLAT Search http://genome.uscs.edu/ FACSDiva Software V6.1.2 BD Beckton Dickinson Fiji image processing package http://www.fji.sc/ Galaxy project in house USCS Genome Browser http://genome.uscs.edu/ High‐throughput Insertion Site Analysis Pipeline (HISAP) in house Ingenuity Pathway Analysis (IPA) http://www.ingenuity.com/ Lasergene DNA Star LightCycler LC480 Software Roche Office 2007 (Word, Excel, PowerPoint) Microsoft Photoshop CS5.1 Adobe R‐Program (2.13.1) cran.r‐project.org
26 MATERIALS AND METHODS
2.2 Methods
2.2.1 Cell Culture Methods
2.2.1.1 Cell Cultivation
A549 (human alveolar basal epithelial cancer cell line), PC3 (human prostate cancer cell line) and U87 (human glioblastoma cell line) were maintained with twice‐weekly subculture in Dulbecco`s Minimal Essential Medium (DMEM) supplemented with 10% fetal calf serum (FCS) and 1% Penicillin/Streptomycin (Pen/Strep). 293THEK (human embryonic kidney cell line) were maintained in IMDM supplemented with 10% FCS and 1% Pen/Strep. Adult normal human dermal fibroblasts (NHDF‐A) were cultivated in DMEM supplemented with 10% FCS, 1% Pen/Strep and 1% L‐Glutamine. NHDF‐A cultivated for more than nine passages were not used for radiation and
chemotherapy experiments. All cells were cultured at 37°C and 5% CO2. For passaging, the adherent cells were washed once with pre‐warmed 1xDPBS and subsequently detached using 3ml or 5ml 0.05% trypsin‐EDTA for a 10cm or 15cm cell culture dish, respectively. The cells were incubated at 37°C in an incubator for 7 minutes. Trypsin activity was blocked by addition of 7ml (10cm cell culture dish) or 10ml (15cm cell culture dish) cell culture medium supplemented with 10% FCS.
2.2.1.2 Freezing and thawing of cells
In order to freeze cells, cell culture freezing medium containing 3ml DMSO, 6ml FCS and 11ml cell culture medium, was prepared. Cells were detached from the cell culture dish, centrifuged at 1,000rpm and room temperature for 5min, and resuspended in cell culture medium. Subsequently, 400ul aliquots were transferred into cryotubes. To each tube, 400µl freezing medium was added, and the tubes placed in freezing boxes. The freezing boxes were stored at ‐80°C over night. Finally, cryotubes were placed in a liquid nitrogen tank. For thawing, cryotubes containing cells were incubated in a water bath for two minutes until they were thawn. Then, cells were resuspended in 10ml cell culture medium in 15ml reaction tubes, centrifuged at 1000rpm for 5min and seeded in cell culture dishes of appropriate size.
2.2.1.3 Cell Counting
For cell counting, 10µl medium containing cells detached from the cell culture dish were transferred to a 1.5ml reaction tube and diluted 1:10 in 90µl trypan blue. From this mixture, 10µl were loaded into a Neubauer counting chamber and the average number of cells in the chamber calculated accordingly: